Abstract

Shootin1 has been ascribed a role in regulating polarization of primary hippocampal neurons. To better understand the possible role of Shootin1 in the developing brain, we identified a member of the kinesin superfamily, KIF20B, as a novel Shootin1 interacting protein and a potential mediator of Shootin1 interaction with microtubules. KIF20B/Shootin1 binding was mapped to a 57 aa KIF20B sequence, which was used as a dominant-negative fragment. Direct interaction between that peptide (MBD) and Shootin1 was confirmed by surface plasmon resonance-based technology and the affinity was determined in the 10−7m range. The proteins are expressed in the developing brain and formed a complex in vivo based on coimmunoprecipitation experiments and coimmunostaining in primary neurons. In primary hippocampal neurons Kif20b knockdown reduced Shootin1 mobilization to the developing axon, as evidenced by immunostaining and fluorescence recovery after photobleaching analysis, suggesting that Shootin1 is a novel KIF20B cargo. shRNA targeting of Shootin1 reduced PIP3 accumulation in the growth cone, as did Kif20b shRNA. In the developing mouse brain, Kif20b knockdown or expression of the KIF20B minimal binding domain inhibited neuronal migration, and in vivo migration assays suggested that Shootin1/Kif20b acts in the same genetic pathway. Time-lapse imaging of multipolar cells in the subventricular zone revealed that downregulating levels of either Shootin1 or Kif20b hindered the transition from multipolar to bipolar cells. Collectively, our data demonstrate the importance of the Shootin1/KIF20B interaction to the dynamic process of pyramidal neuronal polarization and migration.

Analogies have been proposed between polarity regulation of cortical and hippocampal neurons (Watabe-Uchida et al., 2006; Arimura and Kaibuchi, 2007; Reiner and Sapir, 2009). One factor important for the latter is the protein Shootin1 (Toriyama et al., 2006, 2010, 2013; Shimada et al., 2008). Shootin1 protein accumulates in the growing axon during the transition between stages two and three, and its overexpression induces formation of multiple axons, whereas its knockdown inhibits polarization. Shootin1 is also transported to the growth cone in actin-enriched structures (Toriyama et al., 2006). A subsequent study provided evidence for association of Shootin1 with actin flow by demonstrating interaction between Shootin1 and the neuronal cell adhesion molecule, L1CAM (Shimada et al., 2008). Recent studies indicated that within the growth cone, Shootin1 is phosphorylated by Pak1, which resulted in increased interaction between Shootin1 and F-actin retrograde flow, thereby promoting F-actin-substrate coupling, force generation, and concomitant filopodium extension and axon outgrowth (Toriyama et al., 2013).

We identified a member of the kinesin superfamily of proteins, KIF20B, as a novel Shootin1 interacting protein and mapped it to the KIF20B minimal binding domain (MBD). That peptide exhibited high-affinity binding to Shootin1 and acted in a dominant-negative fashion. We found that Shootin1 and Kif20b are highly expressed in the developing mouse brain. Both proteins formed a complex in vivo and partially colocalized in primary neurons along microtubules. Following polymerization and depolymerization cycles of microtubules, Shootin1 was detected in the microtubule-associated protein (MAP) fraction. In developing neurons, Shootin1 and Kif20b knockdown inhibited neuronal migration, and their combined knockdown did not exhibit an additive inhibitory effect, suggesting that they act in a common genetic pathway. Expression of the dominant-negative KIF20B MBD fragment also inhibited neuronal migration. Our results demonstrated that Shootin1 is a novel KIF20B cargo and that interaction with KIF20B localized Shootin1 to the tip of the growing axon. Importantly, reduction in either Shootin1 or KIF20B in multipolar neurons delayed their transition to bipolar neurons. Overall, our analysis indicates that KIF20B and Shootin1 cooperate to regulate polarization of pyramidal neurons in the developing brain.

Materials and Methods

Plasmids.

Full-length Shootin1 (FLCI-Shootin1, AK082304) was obtained from the Mouse Genome Encyclopedia Project of Genome Exploration Research Group in Riken. Three subclones of Shootin1 fragments (S1–S3) were generated in pGEM-Teasy and were used for further subcloning. pRsetB-Shootin1 (S1) was subcloned by BamHI/BglII-XhoI, pCAGG-GFP-Shootin1 (S1) was subcloned by NcoI and EcoRI with an adaptor, and pB27-Shootin1 (S1) and pGEX-4T1-Shootin1 (S1) were cloned by EcoRI and NcoI digestion.

mCherry-Shootin1 (S1) was cloned by SacII and SalI digestion. pRsetA-Shootin1 (S2 and S3) was generated by BamHI/BglII and EcoRI digestion of the corresponding pGEM-Teasy plasmid. Mouse shRNA-Shootin248 (shRNA1) was cloned in pSuper using the following primers: 5′GATCCCCCTGAAGCCTTGGCGACAAATTCAAGAGATTTGTCGCCAAGGCTTCAGTTTTTA and 5′AGCTTAAAAACTGAAGCCTTGGCGACAAATCTCTTGAATTTGTCGCCAAGGCTTCAGGGG.

Mouse shRNA-Shootin1 (shRNA2) was purchased from Open Biosystems TRCN0000071710. Full-length human Shootin1 was purchased from Open Biosystems, clone ID 5169981.

pGEM-Teasy-Shootin1 C-ter was cloned by PCR using the following primers: 5′-AAGAGGCAAGCAGTGGAAGA, 5′-ACAGTTCCTGCCGGTTACAC and cloned into pGEM-Teasy digested by AgeI and SalI. pRsetA-Shootin1-C-ter was subcloned by NcoI and XhoI/SalI of the pGEM-Teasy plasmid. pCAGG-GFP-Shootin1-Cter was generated by digestion of NcoI/NotI and NheI of the pGEM-Teasy plasmid. pCAGG-Human-Shootin1 used for rescue experiments was cloned by KpnI/XhoI and XbaI/NotI of the plasmid purchased from Open Biosystems.

Kif20b plasmids: Kif20b-A15, Kif20b-A7, Kif20b-A20, and Kif20b-A11 were obtained from the yeast two-hybrid screen. Kif20b-A20 was further used to produce Kif20b-MBD using PCR primers: 5′-GAGAATTCGAAAATTCCTTCCAC, 5′-CTCTCGAGTTACTCCTGTGCTCGGAG, pGEX-4T1-Kif20b-A7, pGEX-4T1-Kif20b-A20, pGEX-4T1-Kif20b-A11, and pGEX-4T1-Kif20b-A15 were cloned by EcoRI/NcoI-XhoI restriction digestion. pRsetA-Kif20b was cloned by BamHI and XhoI restriction digestion. Mouse shRNA-Kif20b plasmid was purchased from Open Biosystems, clone ID TRCN0000091234.

GFP-Kif20b-MBD was cloned by EcoRI and XhoI restriction digestion. pGEX-4T1-Kif20b-MBD single mutation (Y1047F) was generated by PCR (with an additional EcoRI site) using the following primers: 5′-GCGACCATCCTCCAAAATC and 5′-GGCCGCTCGAGTTACTCCTGTGCTCGGAGGTCAGAATTCTCCTCCCTGAATCCTTTT. pGEX-4T1-Kif20b-MBD double mutation (Y1047F and R1048A) was generated by PCR using the single mutant plasmid as a template by PCR with the following primers: 5′-GCGACCATCCTCCAAAATC and 5′-GGCCGCTCGAGTTACTCCTGTGCTCGGAGGTCACTGTTCTCCTCCGCGAATCCTTTT. PI-(3,4,5)-trisphosphate (PIP3) was visualized by green fluorescent protein (GFP)-tagged pleckstrin homology (PH) domain of PIP3 interacting protein, Akt (Várnai and Balla, 1998; received from Dr. Tamas Balla, National Institutes of Health, Bethesda, MD).

GFP-Kif20b-MBD-single mutation (Y1047F) was cloned by BamHI/EcoRI and NotI digestion of the corresponding pGEX plasmid. pME-HA-tagged-human KIF20B was received from Masatoshi Hagiwara (Kamimoto et al., 2001).

Rabbit polyclonal anti-Kif20b (serum) was produced against pRSETA-Kif20b-A20. Goat anti-MPP1 was purchased from Santa Cruz Biotechnology (SC-107002). Mouse monoclonal anti-tubulin DM1A was purchased from Sigma (T9026). Mouse monoclonal (hybridoma) anti-hemagglutinin (HA) antibodies were produced by the Weizmann Institute antibody unit. Goat anti-GFP biotinylated was purchased from Abcam (ab6658). The complete open-reading frame of mouse Shootin1 (GenBank accession number gi: 146198590) or the C-terminal region (amino acid residues 413–630) was reverse transcribed from embryonic brain mouse RNA, amplified using PCR, cloned into the pRSET vector (Invitrogen), and the sequence was verified. The Shootin1 protein (S1) (pRSET-Shootin1) was purified using a nickel-agarose column according to the manufacturer's protocol (Qiagen). Antisera to recombinant Shootin1 or Shootin1 C-ter were generated in rabbits and/or rats. Antibodies were verified using Western blot analysis; specificity for immunostaining was tested using pre-incubation with the injected antigen as previously described (Kaplan and Reiner, 2011).

GST pull-down assay.

Recombinant proteins (6×His-tagged Shootin1 proteins) were incubated with 10 Al of GST-tagged proteins at 4°C for 3 h. Glutathione beads (10 ml bed volume) preblocked in T-T buffer supplemented with 10 mg/ml bovine serum albumin (BSA) (Sigma) were added to the protein mixture and rotated for 30 min at room temperature (RT); after four washes with T-T buffer, 2× sample buffer was added, and the beads were boiled and proteins were separated by SDS-PAGE and Western blot analysis.

Microtubule cosedimentation assay.

Bovine brain tubulin obtained from freshly slaughtered calves was purified through two cycles of polymerization–depolymerization, followed by chromatography on a phosphocellulose column and a third cycle of polymerization–depolymerization, as described previously (Williams, 1992; Fygenson et al., 1994). Both recombinant proteins and tubulin were centrifuged at 100,000 g for 30 min to remove protein aggregates. Tubulin was incubated with PEM buffer (80 mm PIPES. pH 6.9, 1 mm MgCl2, 1 mm EGTA), 1 mm GTP, and 10% glycerol at 35°C for 15 min. Taxol or nocodazole were added to the mixture for 15 min at RT or on ice, then the recombinant proteins (histidine tagged-Shootin1 or GST as negative control), diluted in PEM buffer, were added to the mixture for additional incubation of 30 min at RT. The reaction was carefully laid over 125 ml of cushion buffer (50% glycerol in PEM buffer) and centrifuged at 100,000 g for 1 h. Samples of the supernatant were collected and the pellet was washed with PEM buffer and then diluted with concentrated protein sample buffer. The results were analyzed on a 10% SDS PAGE gel followed by Western blotting.

Immunohistochemistry.

Antibodies were used to stain primary neuronal cultures and brain sections. Floating sections or coverslips containing fixed cells were blocked in blocking solution [PBS, 0.1% Triton X-100, 10% HS, 10% fetal calf serum (FCS)] for 30 min. Antibodies were incubated in blocking solution overnight at 4°C. After washing, appropriate secondary antibodies (Jackson ImmunoResearch) were diluted in blocking solution, and incubated for 30 min at room temperature. Slices were mounted onto glass slides using Aqua Poly/mount (Polyscience). Dual immunostaining was performed on primary cortical and hippocampal neurons, which were fixed by immersion in 4% paraformaldehyde (PFA)-PBS for 20 min and then washed three times. The slides were permeabilized for 10 min using PBS containing 0.1% Triton X-100 (PBS/0.1% TX). The slides were blocked with 10% normal horse serum in PBS/0.1% TX for 30 min. Following blocking the slides were incubated overnight in the first rabbit antibody solution. This incubation was followed by three washes in PBS/0.1%TX and a longer incubation (10 min) in PBS. The slides were then incubated in FITC-AffiniPure Fab Fragment Goat Anti-Rabbit IgG (Jackson ImmunoResearch) diluted 1:50 in PBS/0.1%TX, for 2 h at RT. This incubation was followed by five 5 min washes in PBS/0.1%TX followed by a 60 min wash in PBS, then the slides were blocked overnight with a nonconjugated AffiniPure Fab Fragment Goat Anti-Rabbit IgG (H+L) diluted 1:10 in PBS/0.1%TX. Later the slides were washed as previously and incubated with the second rabbit primary antibody at 4°C, overnight. The second primary was thoroughly washed and the slides were incubated in a secondary antibody, Cy3-AffiniPure Donkey Anti-Rabbit IgG (H+L), for 3 h at room temperature. As a precaution, reversal of the order of introduction of the two primary antibodies was performed as well as single immunostaining in which each of the primary rabbit antibodies was used separately.

Yeast two-hybrid analysis.

Yeast two-hybrid screening was performed by Hybrigenics Services, SAS (http://www.hybrigenics-services.com). The coding sequence for Shootin1 (GenBank accession number gi: 146198590) was PCR amplified and cloned into pB27 as a C-terminal fusion to LexA (N-LexA-SHOOTIN-C). The construct was checked by sequencing the entire insert and used as a bait to screen a random-primed mouse embryo brain cDNA library constructed into pP6. pB27 and pP6 derive from the original pBTM116 (Vojtek and Hollenberg, 1995) and pGADGH (Bartel et al., 1993) plasmids, respectively.

Then 130 million clones (17-fold the complexity of the library) were screened using a mating approach with Y187 (mat) and L40Gal4 (mata) yeast strains as previously described (Fromont-Racine et al., 1997). Twenty-eight histidine-positive colonies were selected on a medium lacking tryptophan, leucine, and histidine. The prey fragments of the positive clones were amplified by PCR and sequenced at their 5′ and 3′ junctions. The resulting sequences were used to identify the corresponding interacting proteins in the GenBank database (NCBI) using a fully automated procedure. A confidence score (PBS, for Predicted Biological Score) was attributed to each interaction as previously described (Formstecher et al., 2005).

Further description of the confidence score.

The PBS relies on two different levels of analysis. First, a local score takes into account the redundancy and independency of prey fragments, as well as the distribution of reading frames and stop codons in overlapping fragments. Second, a global score takes into account the interactions found in all the screens performed at Hybrigenics using the same library. This global score represents the probability of an interaction being nonspecific. For practical use, the scores were divided into four categories, from A (highest confidence) to D (lowest confidence). A fifth category (E) specifically flags interactions involving highly connected prey domains previously found several times in screens performed on libraries derived from the same organism. Finally, several of these highly connected domains have been confirmed as false positives of the technique and are now tagged as F. The PBS scores have been shown to positively correlate with the biological significance of interactions (Rain et al., 2001; Wojcik et al., 2002).

Biacore analysis.

SPR was performed on a Biacore 3000 instrument (Biacore), using a CM-5 BIAcore sensor chip (GE Healthcare Bio-Sciences AB). Kif20b was diluted in 100 mm CH3COONa, pH 4.6, to a final concentration of 20 μg/ml, in a total volume of 200 μl and coupled using the standard Biacore amine chemistry protocol. The analyte, Shootin1 (S1), was injected in the running buffer (PBS) at different concentrations at a flow rate of 20 μl/min at 25°C. These conditions resulted in a linear relation between the protein concentration and the maximal (steady-state) response, indicating the pseudo first-order regime in relation to the immobilized ligand. Injections were performed simultaneously over all four channels and blank surface a plain dextran matrix (channel 1) was used as control. The net signal was obtained by subtracting the blank signal from the signal of the immobilized surface. The association phase for Shootin1 binding to Kif20b was followed for 4 min, and the dissociation phases were monitored for 3 min. Surface regeneration between consecutive binding cycles included a 1 min injection of 2 mm NaOH. The response was monitored as a function of time (sensorgram) at 25°C. Multiconcentration data were globally fit using BIAevaluation 3.2 software.

In utero electroporation.

In utero electroporation was conducted as previously described (Sapir et al., 2008a). Four days after electroporation (unless otherwise stated), E18 embryos of either sex were intracardially perfused using 4% PFA-PBS, the brains were postfixed overnight and sectioned. Alternatively, pups were anesthetized and perfused postnatally (P8). The location of treated cells was analyzed in sections by measuring the signal detected in eight bins spanning the width of the cortex from at least four different brains per treatment, and the relative percentage of the signal was compared by ANOVA (Prism 4 for Macintosh; GraphPad Software). Pictures were taken from 60-μm-thick vibratome sections using Zeiss Confocal or Applied Precision DeltaVision microscopy. shRNA constructs including Shootin1 shRNA sequences are pLKO.1. Lentiviral shRNA constructs were purchased form Open BioSystems. Routinely two control shRNAs were used: a pSUPER-based control previously described (Sapir et al., 2008a) and a pLKO.1-TRC (Addgene) control shRNA. The shRNA constructs were coelectroporated with either pCAGGS-GFP or Golgi localization sequence fused to dsRed (a gift from Michael Davidson, Florida). Animal protocols were approved by the Weizmann Institute Institutional Animal Care and Use Committee.

Neuronal cultures.

Cultures were prepared as detailed previously (Goldin et al., 2001). Briefly, mouse embryos (E18) were decapitated and their brains were removed and placed in a chilled (4°C), oxygenated Leibovitz L-15 medium (Invitrogen) enriched with 0.6% glucose and gentamicin (20 μg/ml; Sigma). Hippocampal or cortical tissue was mechanically dissociated and passed to the plating medium consisting of 5% heat-inactivated horse serum, 5% FCS, and B-27 supplement prepared in minimum essential medium (MEM) Earl salts (Invitrogen), enriched with 0.6% glucose, gentamicin (20 μg/ml), and 2 mm glutamax (enriched MEM). Approximately 0.5 ×106 cells were plated in each well of a 24-well plate containing poly-l-lysine/laminin-coated coverslips. Electroporations were done using the NEPA21 electroporation system (Nepa Gene). Adherent cells were electroporated 1 d after plating using CUY900 electrode while suspended cells were electroporated using a cuvette according to the manufacturer recommendations.

Live imaging.

Electroporated brains were harvested 2–3 d after electroporation (E16–E17). Brains were excised in ice-cold L-15 media supplemented with glucose (0.6%), gentamicin (0.02 mg/ml), and oxygen. Brains were embedded in 3.5% low-melt agarose dissolved in L-15 and cut to 300-μm-thick slices by a vibratome. The explants were placed onto Millicell-CM inserts floating on Neurobasal medium supplemented with B27 and N2, 2 mm GlutaMax, 0.5% glucose, and gentamicin. Images were taken 2 h after plating in Applied Precision DeltaVision microscopy equipped with an environmental chamber.

Sparse cell labeling was done as previously described (Matsuda and Cepko, 2007; Morin et al., 2007; Konno et al., 2008) by using pTα-LPL (loxP-polyA-loxP) plasmid containing a poly-adenylation signal flanked by two loxP sites between the Tα1 promoter (Gloster et al., 1999) and the open reading frame. Briefly, shRNA vector, together with the pTα-LPL-LynN-EGFP (MGCIKSKRKD-EGFP; Lyn N-terminal membrane-targeted signal-fused EGFP), and pTα-Cre, were electroporated in utero at E12, and slices were prepared 2 d later. The slices were embedded in a glass-bottom 35 mm culture dish with collagen gel and slice culture was performed as described previously (Miyata et al., 2001). The slices were kept at 37°C in an ONICS humidified incubator chamber (Tokai Hit) on the stage of microscope, with a continuous supply of 45% O2/5% CO2/50% N2 gas. Cross-section images through the glass bottom were acquired with a 40×/0.75 UPLFLN objective lens (Olympus) using a FV-1000 confocal laser scanning microscope system (Olympus). Fluorescence recovery after photobleaching (FRAP) was performed on a Zeiss 510 META confocal microscope. The imaged cultures were maintained at 37°C with the addition of 5% CO2.

Results

Shootin1 interacts with Kif20b

Cell polarization requires the organization of protein complexes in specific subcellular compartments, therefore we hypothesized that Shootin1 works with an additional unknown partner(s). Potential interaction partners were identified by a yeast two-hybrid screen of a mouse embryonic brain cDNA library. Following screening of 130 million clones (17-fold the complexity of the library), 18 high confidence score clones were identified, all representing overlapping or identical fragments of the kinesin superfamily protein Kif20b (schematic presentation of Kif20b and representative clones resulting from the yeast two-hybrid screen are shown in Fig. 1A). Based on these results, we constructed an MBD of 57 aa (amino acid residues 1002–1059), defined by a region common to all positive clones (Fig. 1A). The mapping of interaction domains was facilitated by the generation of C-terminal truncations of Shootin1 (Fig. 1B). Shootin1/Kif20b interaction was verified and mapped using GST pull-down experiments (Fig. 1C). Shootin1 proteins (S1, 1-456; S2, 1-257; and S3, 1-189) were expressed and purified from bacteria as six-histidine fusion proteins, whereas Kif20b fragments (MBD, amino acid residues 1002–1059; A20, amino acid residues 1002–1442; A7, amino acid residues 867–1270) were expressed and purified from bacteria as GST-fusion proteins. Overall, we determined that the first 189 aa of Shootin1 were sufficient to bind all Kif20b fragments tested, whereas the Kif20b MBD was sufficient for Shootin1 association (Fig. 1C).

Shootin1 and Kif20b interaction. A, Schematic presentation of Kif20b and four fragments, which were identified in a yeast two-hybrid screen as interacting with Shootin1. Kif20b-A7 and Kif20b-A20 were further studied biochemically. Kif20b MBD is the minimal common domain to all Kif20b clones found to interact with Shootin1. The motor domain is highlighted in green, and coiled-coil domains are indicated in red. B, Shootin1 long splice form and a series of C-terminal truncations. S1, Shootin1 short splice form; S2, S3, truncated Shootin1; red, predicted coiled coil domain; blue, proline rich domain. C, Pull down of the recombinant Shootin1 short splice form (S1) and C-terminal truncations (S2, S3) by recombinant GST-fusion Kif20b fragments (Kif20b-A7, Kif20b-A20, and MBD). IB, immunoblot. Immunoprecipitation from Shootin1-transfected HEK 293 (D, E) and from E14.5 embryonic brain lysates (F, G). IP, immunoprecipitation; Ex, cell extract; B, beads only control, Ha, control antibodies (anti-HA tag antibodies); C-ter, polyclonal anti-Shootin1 antibodies raised against a C-terminal fragment; Kif20b, polyclonal anti-Kif20b antibodies. H, Surface plasmon resonance (Biacore), measurements of the binding of soluble recombinant Shootin1 S1, (analyte) to immobilized MBD of Kif20b (ligand). I–K, Surface plasmon resonance (Biacore), measurements of the binding of soluble recombinant Shootin1 S1, (analyte) to immobilized wild-type or mutated MBD of Kif20b (ligand). I, Shootin1 bound to wild-type (WT) Kif20b MBD, less Kif20b MBD carrying a single mutation (MBD Y1047F), and very low binding to the doubly mutant Kif20b MBD fragment (MBD Y1047F, R1048A). J, Pre-incubation of different concentrations of Kif20b MBD with Shootin1 inhibits binding to the immobilized Kif20b MBD. K, Pre-incubation of low concentration of doubly mutant MBD does not prevent the binding of Shootin1 to the same surface; however, increased concentrations partially inhibit the binding.

To determine whether the two proteins form a complex in vivo, we undertook immunoprecipitation of HEK293 cells transfected with Shootin1 (Fig. 1D,E). Anti-Kif20b antibodies immunoprecipitated Shootin1, as well as Kif20b itself (Fig. 1D,E). Reciprocally, anti-Shootin1 antibodies immunoprecipitated Kif20b, as well as Shootin1 (Fig. 1D,E). No immunoprecipitated Kif20b or Shootin1 were detected in the absence of specific antibodies (Fig. 1D,E). Immunoprecipitation of brain extracts revealed that two different Shootin1 antibodies immunoprecipitated Kif20b (Fig. 1F), and these two antibodies immunoprecipitated Shootin1 protein (Fig. 1G). Anti-Kif20b antibodies immunoprecipitated endogenous Shootin1 protein and were able to self-immunoprecipitate Kif20b (Fig. 1F).

To further define Shootin1/Kif20b interaction we used the Biacore, a system that measures changes in surface plasmon resonance, which are proportional to the changes in the mass of molecular species bound to the surface (Fägerstam et al., 1992; Jonsson and Malmqvist, 1992; Malmqvist, 1993; Raghavan and Bjorkman, 1995). The Kif20b MBD fragment was immobilized to a sensor chip and the binding of increasing concentrations of recombinant Shootin1 (S1) in the flow through was monitored (Fig. 1H). The equilibrium dissociation (KD) calculated from experimental curves was found to be 1.75E−07m. Overall, these analyses indicate that Kif20b and Shootin1 directly interact. Close inspection of the Kif20b MBD amino acid sequence did not reveal any consensus motifs, which may mediate protein interactions. Yet, since tyrosine residues are known to mediate multiple protein interactions such as sorting signals (Ohno et al., 1995, 1996), we mutated the single tyrosine in that region (Y1047) to phenylalanine (F) and along with an adjacent charged residue (R1048 to A). BIAcore analysis revealed that Kif20b MBD interaction with Shootin1 was reduced following mutation of tyrosine only and the double mutation significantly reduced the interaction (Fig. 1I). We then asked whether the Kif20b MBD might interfere with binding of Shootin1 to Kif20b. Addition of the wild-type Kif20b MBD to soluble Shootin1 prevented Shootin1 binding to the surface (Fig. 1J). However, addition of the doubly mutant Y1047F/R1048A MBD did not have this effect (Fig. 1K). These results indicate that Shootin1 binds Kif20b through the MBD and that binding is dependent on YR residues found at positions 1047/1048.

Kif20b functions have been previously characterized in dividing tissue culture cells, where it was identified as a phosphorylated microtubule associated plus-end-directed molecular motor protein, which is required for proper completion of mitosis (Matsumoto-Taniura et al., 1996; Kamimoto et al., 2001; Abaza et al., 2003). Interestingly, immunostaining of Shootin1 in interphase (Fig. 2A–C) and mitotic HeLa cells (Fig. 2D–F) revealed partial colocalization of Shootin1 with microtubules. Our results confirmed the previously reported immunostaining of Kif20b as punctate dots along interphase microtubules (Fig. 2G–I) and in the midbody (Fig. 2J–L). The partial colocalization of Shootin1 with microtubules promoted us to investigate whether Shootin1 can be detected in the brain MAP fraction. First, we tested the expression of Shootin1 in the developing brain. Immunoblotting detected expression of Shootin1 in cell lysates prepared from mouse cortices: a high molecular weight (∼72 kDa) form of Shootin1 was expressed at low levels at E11, while at later time points (E13, E15, E18, and P2) both lower (∼53 kDa) and higher molecular weight forms were highly expressed (Fig. 2M). These molecular weights correspond to the predicted protein products of long and short splice forms reported in UniProtKB/Swiss-Prot entry Q8K2Q9. Both Shootin1 isoforms were highly enriched in the MAP fraction following cycles of tubulin polymerization and depolymerization and elution from a column using high salt concentration (Fig. 2M). To investigate a potential interaction between Shootin1 and microtubules we performed a cosedimentation assay (Fig. 2N). Purified tubulin was polymerized with the recombinant short isoform of Shootin1 protein in the presence of either the microtubule-stabilizing drug taxol or the microtubule-destabilizing drug nocodazole. The assay relies on the fact that proteins that bind to polymerized microtubules will cosediment through a glycerol-rich cushion following high-speed centrifugation. Following the addition of taxol, the majority of Shootin1 was found in the supernatant and did not cosediment with microtubules, thus suggesting an indirect interaction between Shootin1 and microtubules. The addition of nocodazole reduced the amount of tubulin and Shootin1 proteins detected in the pellet (Fig. 2N). However, the addition of brain-purified MAPs resulted in more Shootin1 detected in the taxol pellet fraction (Fig. 2N), thus suggesting that a MAP(s) is mediating the interaction of Shootin1 and microtubules. We tested whether Kif20b, which is known to bind microtubules directly (Abaza et al., 2003), is also detected in the MAP fraction. In bovine MAP fractions, we can detect both Shootin1 and Kif20b (Fig. 2O). We suggest that Kif20b may be mediating the interaction between Shootin1 and microtubules.

Shootin1 and Kif20b are expressed in the developing brain

To investigate potential functions for Shootin1 and Kif20b in cortical neurogenesis, we asked whether they are expressed in the developing mouse telencephalon. In situ hybridization indicated that Shootin1 mRNA expression was highest in the developing cortical plate (Fig. 2P–R). Shootin1 antibodies also revealed strong immunostaining in the developing cortical plate at E11 and E14 (Fig. 2S,T, respectively). We used anti-Kif20b antibodies we generated as well as commercially available ones (goat anti-MPP1), to immunostain brain slices of E14.5 embryos. Similar expression patterns were noted using both antibodies (Fig. 2U–V vs X,Y). Kif20b was detected in the apical aspect of the ventricular zone, in the marginal zone, in a narrow stripe between the intermediate zone and the cortical plate, and in somewhat lower levels in the cortical plate. Interestingly, midbodies were notable in the ventricular zone, recapitulating our observation in HeLa cells (Fig. 2G–L, Y–AA). To gain information regarding intracellular protein localization during the polarization of cortical neurons, we prepared slices from E14.5 brains that were coelectroporated 2 d earlier with a plasmid carrying Cre, and with a Cre-activated membranal GFP. The labeling of single cells allowed us to locate cells exhibiting multipolar morphology (Fig. 2AB–AE). We noted that in these cells both Kif20b and Shootin1 appeared in dots that were distributed in perinuclear positions. Kif20b was detected in the processes of the multipolar cells with some bias to those pointing toward the pial surface. Shootin1 was detected in multiple processes of the multipolar cells as well in the extending axon. Additionally, we used the same antibodies to stain cultured primary hippocampal neurons, costaining with DMIA (anti-α-tubulin) revealed puncta decorating the microtubules within the growth cones (Fig. 2AF,AH). Furthermore, coimmunostaining of Shootin1 and Kif20b revealed partial colocalization within growth cones of primary hippocampal neurons (Fig. 2AJ–AL). These expression patterns suggest partial colocalization of the two proteins during cortical development, in multipolar cells and in the growth cones of primary hippocampal neurons.

KIF20B mobilizes Shootin1 to the growth cone

KIF20B belongs to the kinesin superfamily of proteins, which includes many microtubule-associated molecular motors. KIF20B has a motor domain in its N-terminal region and thus belongs to the N-kinesins that are known to drive microtubule plus-end-directed motility (for review, see Hirokawa et al., 2009). We postulated that Shootin1 might be a KIF20B cargo. In pyramidal hippocampal neurons transfected with Shootin1-mCherry, we observed Shootin1 in the cell soma and in the growth cone (Fig. 3A-B′). However, when Kif20b was knocked down Shootin1-containing puncta were detected along the axon (Fig. 3C–D′), thus, suggesting a transport defect in these neurons. To gain further insight into the dynamics of Shootin1/KIF20B interaction we conducted FRAP analysis. Primary hippocampal neurons were cotransfected with Shootin1-GFP and either control or Kif20b shRNA or were treated with nocodazole; fluorescence was bleached in the entire growth cone and recovery of GFP intensity was monitored over time. The time of recovery was significantly reduced in the presence of Kif20b shRNA or following treatment with nocodazole (Fig. 3E). The efficiency of nocodazole treatment was verified by immunostaining with anti-tubulin antibodies (data not shown). The time of recovery to a level of 40% of the initial fluorescence signal was more than doubled (control shRNA T40 = 30.6 ± 9.8 vs Kif20b shRNA T40 = 74.1 ± 33, nocodazole T40 = 74.2 ± 20, n = 11). Representative images of two cells demonstrate visible differences in the fluorescence intensity between the two treatments (Fig. 3F–H vs I–K). Therefore, we concluded that KIF20B participates in mobilizing Shootin1 to the growth cone. Furthermore, the effect of nocodazole implies that intact microtubules are required for this mobilization as well as intact actin following treatment with blebbistatin (data not shown, and as previously reported; Toriyama et al., 2006). We postulated that expression of the Kif20b MBD within neurons may interfere with proper mobilization of Shootin1 in the axon. Indeed, live imaging revealed more mCherry-Shootin1 along the axon when Kif20b MBD-GFP was expressed in comparison with GFP or doubly mutated Kif20b MBD (Fig. 3L,M).

Shootin1 transport to the growth cone is Kif20b dependent. Shootin1 transport to the growth cone is Kif20b dependent. A–D′, Hippocampal neurons in culture transfected with GFP, mCherry-Shootin1, and control (A–B′) or Kif20b shRNA (C–D′). Puncta of mCherry-Shootin1 in the growth cone and along the axon are indicated with white triangles. Insert, axonal growth cone of control-treated neurons (B′) and Shootin1 shRNA-treated neurons (D′). E–K, FRAP of Shootin1-GFP at the growth cone. Presented are fitted curves of the average recovery profile of 11 cells, and the average recovery time to 40% of the original signal (T40 in seconds). F–K, Time-lapse images of FRAP analysis (t, time in seconds). White triangles indicate bleached regions. L, M, Kif20b MBD but not double mutated Kif20b MBD affects the distribution of mCherry-Shootin1 along the axon. N, PH-Akt-GFP (PIP3 reporter) localization at growth cones of transfected primary culture of hippocampal neurons treated with control, Shootin1, or Kif20b shRNA. O, The average distribution of PH-Akt-GFP along the growth cone of 29–35 cells. Scale bars: K, 2 μm; L, 3 μm; N, 5 μm.

Shootin1 knockdown was previously shown to reduce localized activity of PI 3-kinase in growth cones of primary hippocampal neurons (Toriyama et al., 2006). We assessed localization of the product of PI 3-kinase activity, PIP3, using the PH domain construct of Akt (Akt-PH-GFP), which specifically interacts with PIP3 in cells, thus acting as a PIP3 sensor (Várnai and Balla, 1998). Our results in primary hippocampal neurons transfected with Shootin1 shRNA confirmed previous findings (Fig. 3N). Kif20b knockdown resulted in less accumulation of the PIP3 sensor in neuronal growth cones (Fig. 3N). Figure 3O shows the plots of average intensity distribution of multiple analyzed cells (n = 30, 35, 29 for control, Shootin1 shRNA, or Kif20b shRNA, respectively). Calculation of correlation coefficients between the intensity and the relative position in the axon indicated greater similarity between Shootin1 and Kif20b shRNA treatments (r2 = 0.45) than between control and Shootin1 treatment (r2 = 0.08) or than between control and Kif20b shRNA treatment (r2 = 0.16). Statistical analysis using ANOVA and Dunnett's multiple-comparison test revealed that the intensity and the relative position in the axon seen following Kif20b shRNA treatment differed significantly from control (p < 0.05). Collectively, our experiments suggest that Shootin1 is a novel KIF20B cargo and that both proteins promote PIP3 accumulation in the growth cone.

Shootin1 and/or Kif20b knockdown inhibit neuronal migration

To further evaluate how Shootin1 and Kif20b may regulate brain development, we acutely transfected combinations of Shootin1, Kif20b, and control shRNAs into the developing mouse brain using in utero electroporation (Fig. 4). Four days after their in utero electroporation, Shootin1 knockdown significantly reduced the proportion of neurons reaching the cortical plate in comparison with control shRNA (Fig. 4B vs A). Shootin1 shRNA specificity was demonstrated by rescue of neuronal migration following coelectroporation of a plasmid-expressing human Shootin1 cDNA resistant to the shRNA sequences (Fig. 4C). Statistical analysis using ANOVA with Tukey's multiple-comparison test revealed that the difference in the position of Shootin1 shRNA versus that of control shRNA was statistically significant in 7 of 10 bins (Fig. 4D). In bins 1 and 5–8 the difference was extremely significant (p < 0.001), and in bins 4 and 9 the difference was very significant (p < 0.01). Rescue by coexpression of human Shootin1 was most evident in six bins (bins 4–9). Shootin1 knockdown also had consequences in postnatal brain (Fig. 4E–G). In mice treated with control shRNA, most cells reached cortical layers II–III; however, in Shootin1 shRNA-treated mice only a fraction of the cells was detected in these layers, while many cells were detected in the deeper layer IV. Cells were also detected in ectopic positions, in the intermediate zone, and in white matter. In control animals, Shootin1 protein was detected in the leading edge of migrating neurons and in the developing axon (Fig. 4H,I). To test whether KIF20B affects neuronal migration and works in concert with Shootin1 in migrating neurons, we monitored the position of migrating neurons for 4 d after in utero electroporation of control shRNA, Kif20b shRNA, Shootin1 shRNAs, a combination of Kif20b shRNA plus Shootin1 shRNAs, or Kif20b shRNA plus a human Kif20b expression plasmid (Fig. 4J–N). Kif20b knockdown in the developing brain impaired neuronal migration. The distribution of Kif20b shRNA-treated cells differed significantly from control (Fig. 4R vs Q unpaired t test: bin 1, p = 0.0001; bin 4, p = 0.001; bin 5, p = 0.004; bin 6, p = 0.003; bin 9, p = 0.01; bin 10, p = 0.04). As noted above, Shootin1 shRNA treatment appeared to significantly impair neuronal migration, more so than treatment with Kif20b shRNA (Fig. 4L,S). However, in animals treated with Shootin1 shRNAs, 4 d postelectroporation the distribution of pyramidal cells along the cortex did not vary from the distribution seen in cells treated with Kif20b shRNA, indicating that both treatments inhibit migration. Furthermore, combining Kif20b and Shootin1 shRNAs did not enhance the effect seen with individual shRNA treatments (Fig. 4M). Coexpression of HA-tagged human KIF20B resistant to shRNA rescued impaired migration seen following Kif20b shRNA treatment (Fig. 4N,U). Human KIF20B expression was verified using immunostaining with anti-HA antibodies (Fig. 4O,P). Overall, these results suggest that KIF20B and Shootin1 act in the same genetic pathway. We further probed the functional interaction between KIF20B and Shootin1 by expressing the Kif20b MBD fragment, which interfered in vitro with Shootin1/KIF20B binding (Fig. 4W), and analyzing the position of GFP-positive cells at stages E14–E17, 3 d after in utero electroporation (Fig. 4V vs W). The position of Kif20b GFP–MBD-expressing cells differed from control cells in a statistically significant manner in four bins (Fig. 4X, bins 1,2,7, and 8). Collectively, our data indicate that KIF20B/Shootin1 interaction is important for proper neuronal migration in the developing cerebral cortex.

Shootin1 knockdown inhibits neuronal migration. A–C, Brain sections from E18.5 mouse embryos, coelectroporated at E14.5 with control shRNA and GFP (A) or with a mixture of Shootin1 shRNA (B). Partial rescue of the migration phenotype following the introduction of shRNA-resistant hShootin1 (C). D, Average signal detected in arbitrary bins along the width of the cortex (bin 1, ventral; bin 10, dorsal). E–G, Brain section from P8 pup treated at E14.5 with control shRNA (E) or a mixture of Shootin1 shRNA (F). G, Cux1 staining (blue) in layers II–IV. H, I, Sections from E16.5 mouse brain sections, 2 d after in utero electroporation showing Shootin1 expression (red) in the leading edge and axon of bipolar neurons. J–N, E18.5 brain sections of E14.4 in utero electroporated mouse brains. Embryos were coelectroporated with GFP and indicated shRNA, Control shRNA (J), Kif20b shRNA (K), Shootin1 shRNAs (L), and a combination of Shootin1 shRNAs and Kif20b shRNA (M). N–P, Partial rescue of the migration phenotype after Kif20b knockdown is achieved after coexpression of shRNA-resistant human Ha-Kif20b. O, P, Expression of shRNA-resistant HA-hKif20b in the base of the leading edge of Kif20b shRNA-treated cells (O and P; Ha red). Q–U, Relative signal in 10 arbitrary bins along the width of cortex measured from 10 sections of 3–4 brains of each treatment (bin 10, the outer part of the cortical plate). V–X, Kif20b–Shootin1 interaction is required for radial migration in the developing cortex. Dominant-negative effect of the GFP-Kif20b MBD in E17.5 brain sections of E14.5 in utero electroporated mouse embryo brains (W) versus GFP alone (V). The relative signal in 10 arbitrary bins along the width of cortex measured from 10 sections of 3–4 brains of each treatment (*p < 0.05). Scale bars: A, 100 μm; G, 200 μm; I, 20 μm; N, 100 μm.

Shootin1 and Kif20b knockdown alters neuronal polarization

Previous studies have demonstrated the role of Shootin1 in polarization of primary hippocampal neurons (Toriyama et al., 2006; Shimada et al., 2008). Therefore, we tested the possible role of Shootin1/Kif20b interaction for polarization of primary hippocampal neurons. Toward that end we transfected primary hippocampal neurons with either control shRNA or control GFP, Shootin1 shRNA, Kif20b shRNA, or Kif20b MBD before their plating on coated slides (Fig. 5A–D, respectively). The cells were allowed to repolarize and were cultured for 4 d. Tracing the outline of the neurons, where the axon (MAP2 negative) is indicated in red, demonstrated a qualitative difference in the structure of the treated neurons. We assessed neuronal polarization by two criteria: measurement of the axon length and counting the number of neurites (Fig. 5E,F). Reduction in the levels of either Shootin1 or Kif20b or interference with Shootin1/Kif20b interaction by expression of the dominant-negative fragment of Kif20b MBD all resulted in impairment of neuronal polarization. Our studies of neuronal migration prompted us to ask whether neuronal polarization in vivo is altered by interference with Shootin1/Kif20b interactions. To do so, we analyzed the multipolar fraction of neurons in utero electroporated at E12.5 and analyzed at E14.5 (Fig. 5G–K). The different time points for electroporation and for analysis were chosen to increase the relative proportion of cells with multipolar morphology. Analysis of 9–13 brain slices demonstrated that both in control and treated cells approximately half the cells are found with multipolar morphology (Fig. 5K). Shootin1 shRNA significantly increased the proportion of multipolar cells in comparison with control shRNA treatment (mean ± SEM, 67.08 ± 3.9% vs 53.24 ± 2.5%, ANOVA, p = 0.022 considered highly significant). Treatments with Kif20b shRNA or Kif20b MBD did not statistically differ from control treatments.

Shootin1 and Kif20b are required for neuronal polarization. A–F, Primary hippocampal neurons prepared from E18 mice embryos were coelectroporated with GFP and either control shRNA, a mixture of Shootin1 shRNA, Kif20b shRNA, or the MBD of Kif20b (Kif20b-MBD fused to GFP). After 4 d in cultures the cells were stained with MAP2 and their morphology was traced. Outline of representative cells are presented, axons are shown in red. E, F, Measurements of the axon length and the number of neurite per cells are presented; *p < 0.05, **p < 0.01. G–J, Inhibition of multipolar to bipolar transition. E12.5 brains were electroporated with Cre-activated Lyn-GFP, Cre, and control shRNA (G), a mixture of Shootin1 shRNA (H), or Kif20b shRNA (I) or Kif20b MBD fused to GFP (J). All embryos were harvested 2 d postelectroporation. Slices were stained with anti-GFP antibodies and the proportion of multipolar and bipolar cells in slices was quantified. K, Pie graphs representing results form 9–13 sections taken from four individual brains. L, M, Time-lapse images from movies showing a pyramidal cell in organotypic slices prepared from E16.5 brains electroporated at E14.5 with control shRNA (L) or Shootin1 shRNA (M). mCherry-Golgi marker in red and membranal GFP in green.

Given the multipolar morphology of most Shootin1 shRNA-treated cells, we asked whether the subset of shRNA-treated neurons that do adopt a bipolar morphology was polarized as well as control neurons. Toward that end, we monitored the position of the Golgi apparatus as a marker of polarity. Studies of primary hippocampal neurons indicate that the Golgi orients toward the forming axon following the accumulation of N-cadherin there (Gärtner et al., 2012). Our time-lapse microscopy showed that the Golgi is motile in polarizing neurons in vivo. However, whereas in control cells the Golgi was always found in the leading edge, in the subset of Shootin1 shRNA-treated cells exhibiting bipolar morphology, the Golgi was not polarized and extended into regions including but not limited to the leading edge (Fig. 5L,M). Collectively, our results suggest that Shootin1 regulates neuronal polarization in migrating neurons.

KIF20B and Shootin1 impair the multipolar to bipolar transition

To enable monitoring of individual cells and dynamic morphology changes using time-lapse microscopy, we titrated the expression of membranal-GFP by the activity of Cre-loxP-mediated recombination (Morin et al., 2007). As described above, electroporation was performed at E12.5 and the brains were sliced 2 d later, at E14.5. Early born postmitotic neurons were labeled with the Tα-1 tubulin promoter (Gloster et al., 1994) driving Cre expression. Our experimental setting resulted in labeling of sparse cells, as they emerge from the ventricular zone; at the beginning of the experiment many cells were multipolar and polarization occurred during the 20 h course of the experiment (Figure 5L, M). Representative images of treated cells at the beginning and end of the 20 h of time-lapse imaging are shown (Fig. 6A–C). Several features were noted following analysis of single cells. At the initial time point, 2 d after electroporation (E12.5–E14.5), most Shootin1 shRNA-treated and Kif20b shRNA-treated cells showed multipolar morphology. These cells exhibited more neurites per cell (mean number of neurites ± SEM, 4.54 ± 0.45, 7.72 ± 0.66, 5.72 ± 0.3 for control shRNA, Shootin1 shRNA, and Kif20b shRNA, respectively, t test of Shootin1 and control p = 0.0007, Kif20b and control p = 0.0374) (Fig. 6D). At an intermediate time point, after 10 h, control cells showed initiation of polarization: the proportion of cells with multiple neurites decreased and the length of the neurites was significantly longer compared with those seen in either Shootin1 shRNA-treated (p < 0.01) or Kif20b shRNA-treated (p < 0.05) cells (Fig. 6E) (40.60 ± 8.53, 21.62 ± 1.63, 23.9 ± 3.88 μm). The mean number of neurites in control-treated cells (3.81 ± 0.44) differed significantly from Shootin1 shRNA-treated cells (6.09 ± 0.88, p = 0.03) and from Kif20b shRNA-treated cells (5.63 ± 0.45, p = 0.009). At the final (20 h) time point, most control cells had completed their polarization: cells appeared to be bipolar with long dendrites and a visible axon (mean number of neurites, 2.81 ± 0.22). In contrast, many Shootin1 shRNA-treated cells remained multipolar with short neurites (mean number of neurites, 6.81 ± 0.71, p = 0.0002). Kif20b knockdown cells exhibited fewer neurites than at the intermediate time point, an observation suggesting that they have the capacity to polarize (4 ± 0.26, p = 0.003). Nevertheless these neurites were relatively short (p < 0.001, 62.20 ± 4.01, 25.1 ± 1.732, 36.56 ± 4.09 for control shRNA, Shootin1 shRNA, and Kif20b shRNA, respectively). At all time points tested, the number of neurites per cell observed following knockdown of either Shootin1 shRNA or Kif20b shRNA was higher than that observed following control treatment (p = 0.024, 0.0156, paired t test, Shootin1 shRNA or Kif20b shRNA vs control, respectively). The polarization of cells in organotypic slices was also monitored by examining the relative angle adopted by the longest processes over time (Fig. 6G–I). At the initial time point, neurites were oriented randomly with no specific angle preference. At the final time point, >80% of control neurites (mostly bipolar cells) were oriented in a manner enabling proper migration such that the leading edge was pointed to the pial surface and the trailing edge toward the ventricle. In cells treated with Shootin1 or Kif20b shRNA, ∼68% of neurites were oriented toward the pial surface. Collectively, our data indicate that knockdown of Shootin1 or Kif20b impairs neuronal polarization, with Shootin1 knockdown being more potent than that of Kif20b knockdown.

In vivo polarization of pyramidal neurons depends on Shootin1 and Kif20b. A–C, Time-lapse images from labeling of neurons in organotypic slices (E14.5). Cells were labeled with Cre-activated membranal GFP (Lyn-GFP) and indicated shRNA at E12.5; representative images were taken at the beginning of the experiment (t = 0) and after 20 h in culture (t = 20). D–F, Measurements of 11 single cells in E14.5 organotypic slices show the distribution of the number of neurites and their length at three time points; 0, 10, and 20 h in culture. G–I, Directionality of the two longest neurites in 10 cells per treatment (G, control shRNA; H, mixture of Shootin1 shRNA; I, Kif20b shRNA) at three time points along the polarization process (t = 0 h, t = 10 h, t = 20 h). The 90° angle indicates the direction of the pial surface; the radius of the circles is 200 μm.

Discussion

The molecular mechanisms underlying early polarization of pyramidal neurons in the developing telencephalon are not completely understood. We chose to examine the roles of Shootin1 in this process since we speculated that in primary cortical neurons in the brain it may act in a way similar to that described for polarization of primary hippocampal neurons (Toriyama et al., 2006, 2010, 2013; Shimada et al., 2008). Shootin1 is highly expressed in the developing brain and its expression pattern resembles that of other genes known to govern neuronal migration such as Dcx (Francis et al., 1999). Shootin1 knockdown inhibited neuronal migration, and neurons retained a multipolar morphology for an extended period of time. Furthermore, defects in polarization were evident by the position and lack of clustering of the Golgi apparatus.

Schematic presentation of the role of Kif20b and Shootin1 in neuronal polarization. A, The molecular motor KIF20B (blue) mobilizes Shootin1 (pink or red stars) and PIP3 vesicles (purple structures) to the growth cone toward the plus ends of microtubules. Shootin1 is mobilized along the microtubules (green) and it is deposited at the basis of the growth cone. The front edge of the growth cone is actin rich (orange fibers). Shootin1 also complexes with PI 3-kinase, which produces local PIP3 in the growth cone. At the growth cone Cdc42 and Rac1 induce Pak1-mediated Shootin1 phosphorylation (red stars). PAK1 phosphorylated Shootin1 enhances the “clutch” engagement through interaction with L1CAM (green) and F-actin. B, Polarization of pyramidal neurons in the developing cortex relies on Shootin1 and KIF20B. Multipolar cells at the intermediate zone (IZ) are retracting processes and elongating a future axon (thin green line) and a predominant basal process. The polarized cells invade the cortical plate (CP). Shootin1 knockdown causes cells to appear highly branched and to spend longer periods of time in the IZ at the multipolar stage. Kif20b knockdown partially recapitulates this phenotype.

KIF20B, a mitotic kinesin

Our unbiased yeast two-hybrid screen detected a candidate MAP for mediating the Shootin1/microtubule interaction, KIF20B, a member of the kinesin superfamily of microtubule-associated motor proteins (Miki et al., 2005; Hirokawa et al., 2009). The interaction between the two proteins required the N-terminal part of Shootin1 and a short tyrosine-containing peptide of KIF20B (termed MBD amino acids 1002–1059). This interaction does not overlap with the Shootin1/actin interaction domain, which mapped to a C-terminal part of Shootin1 (Shimada et al., 2008). KIF20B is primarily known as a mitotic kinesin. It is heavily phosphorylated during mitosis and was first identified as one of the MPM2 antigens (Westendorf et al., 1994). Later studies demonstrated that KIF20B exhibited microtubule-dependent molecular motor activities and binding to microtubules, and was required for completion of cytokinesis (Abaza et al., 2003). During mitosis it interacts with PIN1 and PRC1 (Kamimoto et al., 2001; Kanehira et al., 2007). Nevertheless, so far its role in neuronal cells has not been studied, although it has been postulated that KIF20B may function in postmitotic neurons due to the presence of auto-antibodies of this protein in patients with idiopathic ataxia (Fritzler et al., 2000; Zochodne et al., 2003). As a member of the kinesin superfamily, it may participate in polarization regulation through transport of specific cargoes. Some cargoes may be transported by one kinesin, while others may be transported by more than one molecular motor to deliver them to the correct subcellular localization. For example, synaptic vesicle precursors are transported by KIF5 and KIF1A or by KIF1B, but NMDA receptors are transported by KIF17 (for review, see Hirokawa et al., 2009). Our study indicates that KIF20B mobilizes Shootin1 (Fig. 7A). Furthermore, in agreement with previous findings (Toriyama et al., 2006), PIP3 accumulation to neuronal growth cones was impaired following Shootin1 knockdown. Kif20b knockdown also produced a similar phenotype. Previously, it has been demonstrated that PIP3 accumulation in a cell's longest neurite induced its development into an axon (Shi et al., 2003; Ménager et al., 2004). One demonstrated mechanism underlying PIP3 accumulation at the tip of the axon is its motor-dependent transport by GAKIN, also known as KIF13B, via its interaction with the adaptor protein PIP3BP/centaurin-α (Horiguchi et al., 2006). An additional possibility may be through activation of upstream PI 3-kinase signaling (Aoki et al., 2005). It was previously demonstrated that Shootin1 interacts with PI 3-kinase and is required for localized PI 3-kinase activity in growth cones of hippocampal neurons (Toriyama et al., 2006). Our studies demonstrated that PIP3 accumulation includes not only increased localized activity of the kinase but also transport, which is mediated by KIF20B (Fig. 7A).

Our findings demonstrated that both Shootin1 and KIF20B regulate radial migration within the developing telencephalon (Fig. 7B). Among multiple mitotic kinesins, it has been suggested that KIF15 participates in regulation of neuronal migration based on its expression pattern and subcellular localization (Buster et al., 2003). In addition, KIF11 has been demonstrated to regulate migration of cortical neurons (Falnikar et al., 2011). Those authors and others (Haque et al., 2004; Yoon et al., 2005; Myers and Baas, 2007) have suggested that KIF11 acts as a brake on interactions between microtubules in developing neurons. KIF11 depletion or inhibition in cultured sympathetic neurons resulted in faster growing axons, which did not turn properly (Nadar et al., 2008). KIF11 knockdown in pyramidal neurons resulted in faster migration, and conversely its overexpression inhibited neuronal migration (Falnikar et al., 2011). Thus, the mechanism of action of KIF20B is very different from that of Kif11. We propose that following either Kif20b knockdown, which perturbs Shootin1 transport, or Shootin1 knockdown, neuronal migration and polarization are impaired.

Shootin1/KIF20B polarity proteins

Shootin1 belongs to a growing list of proteins that regulate neuronal polarization and function in regulation of neuronal migration. MARK2/Par-1 regulates neuronal polarity in cultured neurons (Biernat et al., 2002; Chen et al., 2006; Terabayashi et al., 2007). In vivo, MARK2/Par-1 affects the multipolar to bipolar transition (Sapir et al., 2008a), radial neuronal migration to the cerebral cortex (Sapir et al., 2008a), and the rostral migratory stream to the olfactory bulb (Mejia-Gervacio et al., 2012). In radially migrating neurons, one function of MARK2/Par-1 is to phosphorylate DCX (Sapir et al., 2008b). Our results show the importance of the Shootin1/Kif20 polarity complex in migrating neurons. Whereas the role of Shootin1 in regulation of polarization of primary hippocampal has been documented (Toriyama et al., 2006; Shimada et al., 2008), we show here that Kif20b and Shootin1/Kif20b are also important in polarization of primary hippocampal neurons as well as in regulation of polarization and migration of pyramidal neurons (Fig. 7B). Furthermore, our studies ascribe new polarity functions for KIF20B, which in primary hippocampal neurons mediates the transport of Shootin1 and PIP3, and in migrating neurons is involved in regulation of polarization and migration (Fig. 7B). Our data suggest that Shootin1/KIF20B not only form a complex, but also act in the same genetic pathway. Knockdown of either one impairs neuronal migration, where the effect of Shootin1 knockdown was more robust than that of KIF20B, and the combined effect of both treatments did not result in a synergistic effect. The impact of Shootin1-KIF20B interaction was also demonstrated by expression of the MBD of KIF20B, which also impaired neuronal migration.

Our in vivo analysis clearly supports a role for Shootin1 and KIF20B in the important multipolar to bipolar transition. We assessed several polarization features: control cells exhibited progressive decline in the number of neurites, and remaining neurites lengthened and oriented along the migration axis. Shootin1shRNA-treated or Kif20b shRNA-treated cells exhibited more and shorter neurites, which were less oriented. Shootin1 knockdown cells were more strongly impaired, suggesting Shootin1 may function to regulate additional, unidentified molecule(s) governing the polarization process.

Footnotes

O.R. is an Incumbent of the Berstein–Mason professorial chair of Neurochemistry. Our research has been supported in part by the Israel Science Foundation (Grant no. 47/10), the Minerva foundation with funding from the Federal German Ministry for Education and Research, a grant from the Chief Scientist Office at the Israeli Ministry of Health under the frame of ERA-Net NEURON (DISCover, IMOS 3-00000-6785), the Fritz–Thyseen Foundation (Grant Az. 10.11.2.161), the Benoziyo Center for Neurological diseases, the Helen and Martin Kimmel Stem Cell Research Institute, and the David and Fela Shapell Family Center for Genetic Disorders Research. We thank Dr. Ilya Soifer for help with the analysis and Drs. Michael W. Davidson, Tamas Balla, and Masatoshi Hagiwara for providing us with useful plasmids.